Comparative neuroanatomy suggests repeated reduction of neuroarchitectural complexity in Annelida
© Heuer et al; licensee BioMed Central Ltd. 2010
Received: 15 February 2010
Accepted: 4 May 2010
Published: 4 May 2010
Paired mushroom bodies, an unpaired central complex, and bilaterally arranged clusters of olfactory glomeruli are among the most distinctive components of arthropod neuroarchitecture. Mushroom body neuropils, unpaired midline neuropils, and olfactory glomeruli also occur in the brains of some polychaete annelids, showing varying degrees of morphological similarity to their arthropod counterparts. Attempts to elucidate the evolutionary origin of these neuropils and to deduce an ancestral ground pattern of annelid cerebral complexity are impeded by the incomplete knowledge of annelid phylogeny and by a lack of comparative neuroanatomical data for this group. The present account aims to provide new morphological data for a broad range of annelid taxa in order to trace the occurrence and variability of higher brain centers in segmented worms.
Immunohistochemically stained preparations provide comparative neuroanatomical data for representatives from 22 annelid species. The most prominent neuropil structures to be encountered in the annelid brain are the paired mushroom bodies that occur in a number of polychaete taxa. Mushroom bodies can in some cases be demonstrated to be closely associated with clusters of spheroid neuropils reminiscent of arthropod olfactory glomeruli. Less distinctive subcompartments of the annelid brain are unpaired midline neuropils that bear a remote resemblance to similar components in the arthropod brain. The occurrence of higher brain centers such as mushroom bodies, olfactory glomeruli, and unpaired midline neuropils seems to be restricted to errant polychaetes.
The implications of an assumed homology between annelid and arthropod mushroom bodies are discussed in light of the 'new animal phylogeny'. It is concluded that the apparent homology of mushroom bodies in distantly related groups has to be interpreted as a plesiomorphy, pointing towards a considerably complex neuroarchitecture inherited from the last common ancestor, Urbilateria. Within the annelid radiation, the lack of mushroom bodies in certain groups is explained by widespread secondary reductions owing to selective pressures unfavorable for the differentiation of elaborate brains. Evolutionary pathways of mushroom body neuropils in errant polychaetes remain enigmatic.
Annelida is an ancient phylum that comprises over 16,500 described species. Its members inhabit nearly all biotopes in marine environments, and occupy fresh water and moist terrestrial habitats . Traditionally, the segmented worms are thought to fall into two major groups: Polychaeta (bristleworms) and Clitellata (worms with a specialized reproductive structure, the clitellum). Among them, Polychaeta represents the larger and more diverse taxon, a fact that can be attributed to the high evolutionary plasticity of the polychaete body plan. In different groups, head appendages (prostomial palps and tentacles, peristomial cirri) and body appendages (parapodia) have been modified in numerous ways to suit a wide range of lifestyles and feeding strategies, including active predation, scavenging, deposit and suspension feeding. Clitellata, in contrast, lack elaborate head and body appendages and thus show less diverse body forms. While ectoparasitic members of the Hirudinea (leeches) have a specialized feeding apparatus that allow them to feed on the body fluids of their hosts, other clitellates can be characterized as predators, detritivors or direct deposit feeders.
Surprisingly, evolutionary relationships within this ecologically important metazoan phylum are still poorly understood [2–4]. Clitellatesare g enerally accepted to form a monophyletic clade, but phylogenetic relationships within the group are still a matter of debate . Polychaete relationships represent one of the most intractable problems of phylogenetic research  and the history of polychaete systematics is accordingly long and convoluted [reviewed in ]. The most influential traditional concept divided the group into the orders Sedentaria and Errantia . This division was later recognized as a rather arbitrary grouping , useful for practical purposes but not representing correct phylogenetic relationships. Due to the lack of conclusive evidence, many authors subsequently refrained from grouping the approximately 80 well-established polychaete families into higher-ranking taxa. Analyzing morphological character traits across a broad range of families, Rouse and Fauchald  provided one of the most comprehensive cladistic studies to date. They proposed the Polychaeta to form two major clades, Scolecida and Palpata, the latter comprising the Canalipalpata (containing the remainder of the Sedentaria) and the Aciculata (containing the remainder of the Errantia). However, not all of these groups are strongly supported [10, 11] and their monophyly has been questioned by morphological [12, 13] as well as molecular studies [2, 4, 14]. As yet, a conclusive phylogeny for the segmented worms is still lacking and annelid systematics remain "one of the most vexing problems in invertebrate phylogenetics" [, page 1462].
Searching for novel characters to advance the reconstruction of annelid relationships, several authors have looked into the architecture of the central nervous system. The metameric organization of the ventral nerve cord in developing stages of Bonellia viridis led Hessling  to propose the inclusion of echiurids into the Annelida. Similarly, segmental patterns observed during neurogenesis of Phascolion strombus and Phascolosoma agassizii indicate a close affinity of Sipuncula and Annelida. Detailed investigations into the neuroarchitecture and the internal scaffolding of the central nervous system across a wide range of polychaete species were provided by Orrhage and Müller . Drawing on innervation patterns, these authors postulated homology hypotheses for the highly variable head appendages encountered in different polychaete species. In a similar approach, Zanol and Fauchald  presented in-depth neuroarchitectural descriptions of eunicid polychaetes to elucidate evolutionary transformations of the head appendages in this group.
Materials and methods
List of investigated annelid species, including collection sites, ecological background information from sampling localities and literature as well as number of investigated specimens.
Habitat, depth, sampling locality
(from Fauchald and Jumars)
Underneath rocks, 5 m, Cala Olivera, Ibiza (2006, 2007)
Slow-moving carnivore, epibenthic
Infaunal, on tidal flats, Königshafen, Sylt (2008)
Detritus feeder, burrowing
On algae-incrusted rocks, 2-10 m, Cala Llenya, Cala Olivera, Ibiza (2007)
Suspension feeder, tube-dwelling
In crevices and adjacent detritus, 1-15 m, Cala Llenya, Cala
Olivera, Cala Vedella, Penyal de s'Aguila, Ibiza (2006, 2007)
Attached to bottom side of rocks, 1-6 m, Cala Llenya, Cala Olivera, Cala Vedella, Ibiza (2006, 2007)
Detritus feeder, tube-dwelling
Underneath rocks, 1-6 m, Cala Olivera, Penyal de s'Aguila, Ibiza (2006, 2007)
Underneath rocks, 1-10 m, Cala Llenya, Cala Olivera, Ibiza (2007)
Purchased at a local pharmacy, Aachen
On algae-covered rocks, 1-10 m, Cala Olivera, Penyal de s'Aguila, Ibiza (2006, 2007)
Purchased from a local vendor, Aachen
Detritus feeder, burrowing
Lumbrineris cf. fragilis
Infaunal, 90-200 m, Raunefjord, Hjeltefjord, Bergen (2008)
in silt, 90-200 m, Raunefjord, Hjeltefjord, Bergen (2008)
Infaunal, on tidal flats, Königshafen, Sylt (2008);
in silt, 90-200 m, Raunefjord, Hjeltefjord, Bergen (2008)
Carnivorous, motile burrower
Infaunal, on tidal flats, Königshafen, Sylt (2008).
Additional specimens, kindly provided by J. von Döhren, were
collected on the isle of Helgoland (Germany)
Odontosyllis cf. fulgurans
(AUDOUIN & MILNE-EDWARD, 1833)
On algae-incrusted rocks and in silt samples, 90-200 m, Raunefjord, Hjeltefjord, Bergen (2008)
Infaunal, 3-12 m, Cala Llenya, Ibiza (2006, 2007)
Infaunal, on tidal flats, Königshafen, Sylt 2008
Hunting predator/scavenger, free-living
Attached to hard substrates and in silt, 90-200 m, Raunefjord, Hjeltefjord, Bergen (2008)
Detritus feeder, tube-dwelling
Clump of tubes recovered from a silt sample, 90-200 m, Raunefjord, Hjeltefjord, Bergen (2008)
Suspension feeder, tube-dwelling
In silt, 90-200 m, Raunefjord, Hjeltefjord, Bergen (2008)
Sthenelais cf. limicola
Infaunal, 3-12 m, Cala Llenya, Ibiza (2007)
Attached to rocks and in silt, 90-200 m, Raunefjord, Hjeltefjord, Bergen (2008)
Detritus feeder, tube-dwelling
Two specimens recovered from a dredge sample, Raunefjord, Hjeltefjord, Bergen (2008)
In short, annelid heads - or, for L. maderae, dissected brains - were fixed overnight in 4% paraformaldehyde in 0.1 M phosphate buffered saline (PBS) at room temperature. Prior to paraformaldehyde fixation, specimens intended for anti-histamine immunohistochemistry were fixed overnight in 4% carbodiimide (1-Ethyl-3-(3-dimethylaminopropyl)-carbodiimide hydrochloride; Sigma-Aldrich, Steinheim, Germany) in PBS.
For vibratome-sectioning (VT1000S, Leica Microsystems, Wetzlar, Germany), the tissue was rinsed in four changes of PBS and then embedded in a gelatine/albumin medium. After hardening for 16-18 h in 15% formalin in PBS at 8°C, the gelatine/albumin blocks were cut into sections of 80-100 μm thickness. The sections were washed in six changes of PBS with 0.1% Triton X-100 (TX) and subsequently pre-incubated overnight in a blocking solution of 500 μl PBS containing 0.5% TX and 5% normal swine serum (Jackson ImmunoResearch, West Grove, PA). Primary antibodies were added directly to the blocking solution: anti-FMRF-amide (ImmunoStar, Hudson, WI) at a dilution of 1:20000, anti-serotonin (Sigma-Aldrich, Saint Louis, MO) at a dilution of 1:20000 or anti-histamine (Progen Biotechnik, Germany) at a dilution of 1:50000. Specificity controls for the antibodies were performed by the suppliers by liquid-phase preabsorption of the diluted antisera with 100 μg/ml of FMRF-amide, 200 μg/ml serotonin conjugated to bovine serum albumin, or 10-100 μg/ml histamine, respectively. Immunostainings were completely abolished by these pretreatments. After 26 h of incubation at room temperature, sections were washed in six changes of PBS with 0.1% TX. They were then transferred to 500 μl PBS containing 0.5% TX and 1% normal swine serum. Secondary antibodies (Jackson ImmunoResearch, West Grove, PA) at a dilution of 1:2000 were added directly to this solution and incubated for approximately 16 h at room temperature. Afterwards, the secondary antiserum was removed and the sections were incubated with the nuclear marker DAPI (4',6-Diamidino-phenylindole, dilactate; Sigma-Aldrich, Steinheim, Germany) at a dilution of 1:1000 in PBS for 12 min. Subsequently, sections were rinsed again in several changes of PBS containing 0.1% TX and then mounted on chrome alum/gelatine-coated glass slides under glass coverslips using Elvanol (mounting medium for fluorescent stainings after Rodriguez and Deinhard ).
Preparations were analysed with a confocal laser-scanning microscope (TCS SP2, Leica Microsystems, Wetzlar, Germany). A helium/neon laser (excitation wavelength 543 nm, detection range 555-700 nm) was used to detect Cy3 fluorescence, DAPI fluorescence was detected with a diode-laser (excitation wavelength 405 nm, detection range 410-550 nm). Autofluorescence of the tissue was visualized with the argon/krypton laser (excitation wavelength 488 nm, detection range 500-535 nm). Confocal images were finally processed using global imaging enhancement procedures (contrast, brightness) and superposition functions of 'Adobe Photoshop CS'.
Three-dimensional surface reconstruction of cerebral neuropils in Lepidonotus clava followed the protocol described in Heuer and Loesel  (2009). Using the Amira graphics software package (Mercury Computer Systems Inc., Chelmsford, MA) and a graphic tablet (Intuos3 from Wacom, Krefeld, Germany), neuropil models were rendered from a manually labeled data set of 252 consecutive optical sections in a single, well-preserved specimen.
Arenicola marina (Arenicolidae, Scolecida, Polychaeta)
The brain of the lugworm A. marina is formed by the dorsal convergence of the paired circumesophageal connective. It consists of two fiber masses that are clearly separated from each other and are only posteriorly connected by sparse fibers bundles (Fig. 3a). The brain does not contain distinct subcompartments. Neuronal somata reside dorsally and laterally of the fiber masses; conspicuous aggregations of small diameter cells are not apparent.
Ophelia limacina (Opheliidae, Scolecida, Polychaeta)
O. limacina is an infaunal substrate-feeding species with a small, cone-shaped prostomium. The brain has an oval to round shape and is situated between two cerebral eyes (Fig. 3b). It does neither contain lobed neuropils nor any other distinct subcompartments. Instead, serotonin- and FMRF-immunoreactivity reveal the brain to consist of an undifferentiated neuropil tangle that is surrounded by medium to large-sized neuronal somata. Additionally, two populations of comparatively small cell bodies are located bilaterally of the posterior part of the neuropil. They form a pair of cone-shaped, laterally tapering aggregations that encase small protuberances of the central neuropil.
Scalibregma inflatum (Scalibregmatidae, Scolecida, Polychaeta)
In the sediment-dwelling species S. inflatum, the brain is located in the middle of the T-shaped prostomium (Fig. 3c). It consists of a central neuropil that is dorsally and laterally covered by neuronal somata. While numerous of these somata exhibit FMRF-like immunoreactivity, serotonin immunoreactivity is restricted to a limited number of cell bodies, most of which are located to both sides of the brain at its anterior-posterior midline (Fig. 3c). The central neuropil forms a compact fiber mass anteriorly, which gradually tapers into two medially separated lobes posteriorly. Distinct neuropil substructures are not distinguishable within the fibrous meshwork. Laterally of the posterior lobes, loosely packed aggregations of small cell bodies occupy the dorsal part of the prostomium. The border of these cell clusters is diffuse and they are not invaded by protrusions of the central neuropil, nor do they surround any neuropil components.
Eupolymnia nebulosa (Terebellidae, Canalipalpata, Polychaeta)
The brain of the sedentary polychaete species E. nebulosa is situated above the pharynx and has a ribbon-like shape (Fig. 3d). It is confluent with - and hardly distinguishable from - the circumesophageal connectives, thus forming a ring-shaped neuronal mass around the pharynx (a similar condition is observed in Thelepus cincinnatus, see Fig. 7c-h). The brain itself consists of a neuropil band, which is dorsally and posteriorly covered by neuronal somata. The neuropil band is formed by a meshwork of tangled neurites. Immunoreactivity towards different antisera reveals a distinct stratification within the neuropil band (Fig. 7a, b), possibly reflecting functional subdivisions of the brain.
Sabella penicillus (Sabellidae, Canalipalpata, Polychaeta)
The feather duster worm S. penicillus is a tube-dwelling filter feeder. The brain of this sedentary polychaete is located at the base of the tentacle crown. It is composed of two bilaterally arranged fiber masses that are dorsally connected by a narrow neuropil band (Fig. 4a). The neuropil appears undifferentiated and contains no distinct subcompartments. Neuronal somata cover the brain neuropil laterally and dorsally but do not form conspicuous aggregations.
Similar neuroanatomical conditions are exhibited by the closely related sabellid species Branchiomma bombyx (Fig. 8b).
Tomopteris helgolandica (Tomopteridae, Aciculata, Polychaeta)
In the pelagic predator T. helgolandica, the brain is situated between a pair of simple lens- eyes at a posterior position in the prostomium (Fig. 4b). The brain has an oval to rectangular shape and consists of an undifferentiated central neuropil which is covered by medium-sized neuronal somata on its dorsal side. At the posterior margin of the brain, two roughly hemispherical aggregations of small-diameter cell somata are discernable. These globuli cell clusters surround small protrusions of the central neuropil that are partly invaded by serotonin-immunoreactive fibers (Fig. 10d). There is no evidence for lobed neuropils associated with the globuli cell aggregations within the central neuropil.
Nereis diversicolor (Nereididae, Aciculata, Polychaeta)
The neuroanatomy of N. diversicolor has already been described in detail in an earlier account . The brain has a roughly trapezoid shape and is located between the two pairs of eyes at a posterior position in the prostomium (Fig. 4c). The most prominent structures in the brain of N. diversicolor are two aggregations of globuli cell somata that give rise to clearly demarcated mushroom body neuropils (Fig. 1). They are situated at the dorsal, anterior part of the brain and form a larger anterior and a smaller posterior cluster. They surround the apical parts of the mushroom body neuropil, which forms finger-like protrusions within the globuli cell aggregation. Emanating ventrally from the globuli cells, the protrusions merge into a massive stalk, which bends towards the center of the brain to form two terminal lobes. Associated with the mushroom body neuropils are two clusters of poorly distinguishable glomerular neuropils which receive sensory input from the prostomial palps. The second distinctive subcompartment in the brain of N. diversicolor is the optic neuropil. Connecting the four eyes of the animal, the dense neuropil resembles an 'H' with its vertical lines bended outwards [compare ]. While its middle part is divided into an anterior and a posterior layer, the optic neuropil is otherwise devoid of neuroarchitectural substructures. Adjacent to the optic neuropil, histamine immunoreactivity reveals an additional unpaired midline neuropil consisting of a crescent-shaped, undifferentiated fiber tangle (Fig. 11b). However, evidence for a possible connectivity between this small, crescent-shaped neuropil and the optic neuropil is lacking.
Phyllodoce maculata (Phyllodocidae, Aciculata, Polychaeta)
The brain of the predatory and highly motile paddle-worm P. maculata is situated between - and slightly anterior of - the two eyes of the animal (Fig. 4d). The dorsal part of the brain comprises a dense tangle of neurites that derive from peripherally arranged neuronal somata. Cell nuclei labeled sections reveal two aggregations of comparatively small cell bodies anteriorly of the central neuropil. As the cell bodies form only a loose assembly, the borders of the cell clusters appear rather diffuse. Ventrally, two thick stalk-like fiber-bundles emanate from the globuli cell clusters and enter the brain (Fig. 10c). They extend posteriorly and then, at the level of the eyes, bend inwards. In bending towards the center of the brain, the stalks appear to split into two parts. Poorly delineated from the rest of the neuropil, these parts are possibly confluent with their contralateral counterparts.
Nephtys hombergii (Nephtyidae, Aciculata, Polychaeta)
The brain of the free-living, predatory polychaete N. hombergii is displaced posteriorly and occupies a position between the prostomium and peristomium. It has a roughly trapezoid shape and is flanked by a pair of cerebral eyes posteriorly (Fig. 5a). The central part of the brain comprises a largely undifferentiated neuropil which gives rise to the circumesophageal connectives anterio-laterally. A pair of poorly delineated neuropil subcompartments is situated dorsally of the roots of the circumesophageal connectives (Fig. 10b). Barely discernable, these two oval-shaped neuropil regions lie adjacent to aggregations of small diameter cell bodies located at the anterio-lateral borders of the neuropil. In contrast to the neuropil regions, the globuli cell clusters are well defined and exhibit a sharp boundary.
Eunice torquata (Eunicidae, Aciculata, Polychaeta)
In the carnivorous species E. torquata, the brain is located at an anterior position in the prostomium. The neuropil consists of a main fiber mass that is situated between the eyes of the animal and two anterior lobes lying in front of that fiber mass (Fig. 5b). Immunoreactivity towards FMRF-amide and histamine antisera is largely restricted to the main part of the brain, with the anterior lobes exhibiting only a comparatively weak signal. While neurites in the main fiber mass form a tangled meshwork for the most part, histamine as well as FMRF-like immunoreactivity reveal individual fibers to form an unpaired midline neuropil (Fig. 11c). The midline neuropil is slightly curved posteriorly and comprises distinct columnar components that connect two commissural fiber bundles.
In E. toquata, a huge mass of densely assembled, minute cell bodies is situated in front of the brain. Dorsally, these somata form an unpaired aggregation that is divided into an anterior and a postior part. In contrast to the anterior part, many cells of the posterior part exhibit FMRF-like immunoreactivity. Proceeding ventrad, the posterior part gradually diminishes, and the anterior part separates to form bilaterally paired clusters that surround the anterior lobes. Despite the presence of a large aggregation of minute cells, neither the main part of the brain, nor the anterior lobes contain distinct subcompartments.
Lumbrineris cf.fragilis (Lumbrineridae, Aciculata, Polychaeta)
The brain of the infaunal selective deposit feeder L. cf. fragilis is situated at a posterior position in the cone-shaped prostomium. It is composed of a main neuropil and a set of large anterior and small posterior lobes (Fig. 5c). The cerebral neuropil is almost completely enveloped by a cortex of small-diameter cell bodies. The densely packed somata form confluent aggregations that surround the anterior lobes, the main neuropil, and the posterior lobes on all sides (Fig. 10f). They do, however, not give rise to any distinctive neuropil substructures. Individual cell bodies in the surrounding cell cortex show immunoreactivity withantisera directed against FMRF -amide and serotonin. Immunopositive cell bodies were observed to be associated with all three parts of the brain, but were most numerous in the posterior lobes. Immunoreactivity within the neuropil was most pronounced in the central part of the brain, where commissural fiber tracts and large parts of the neuropil were stained (Fig. 10f). Strong immunostaining could also be observed in the posterior lobes. In contrast, antisera produced only faint and scattered immunostainings in the anterior lobes.
Odontosyllis cf. fulgurans (Syllidae, Aciculata, Polychaeta)
The brain of O. cf. fulgurans, a predator with a bioluminescent epitokous form, is situated in the anterior part of the prostomium and is located between the eyes of the animal (Fig. 5d). It comprises a triangular to diamond-shaped fiber mass that appears largely undifferentiated and contains no discernable subcompartments, as well as peripherally arranged neuronal somata. Cell nuclei labeled sections show two aggregations of minute cells in each hemisphere. They form a wedge-shaped anterior cluster between the eyes and the anteriorwall of the prostomium, and a posterior cluster situated laterally behind the eyes (Fig. 10e). The anterior clusters encase small, branching protuberances of the neuropil. In a similar fashion, the neuropil also sends out extensions towards the posterior clusters.
Hesione pantherina (Hesionidae, Aciculata, Polychaeta)
The brain of the carnivorous H. pantherina is situated roughly in the middle of the prostomium and is flanked by two pairs of eyes posteriorly (Fig. 6a, Fig. 9a-d). The cerebral fiber massis well differentiated. Its dorsal part contains two elaborate neuropils that are associated with paired aggregations of minute cell bodies situated in front of the anterior eyes (Fig. 9a, b). The neuropils have a stem-like shape, formed by the fusion of several lateral branches that converge towards the midline of the brain. The lateral branches of the neuropil exhibit FMRF-like immunoreactivity. FMRF-amide antiserum also produces characteristic patterns in the rest of the dorsal fiber mass. Ventrally, the cerebral fiber mass is divided into almost completely separated hemispheres (Fig. 9c, d). The hemispheres are laterally and posteriorly surrounded by densely assembled cell bodies. These aggregations appear to be confluent with the dorsal globuli cell clusters and give rise to distinct, converging fiber bundles that merge with the main fiber mass. Small clusters of poorly demarcated spheroidal compartments are barely distinguishable in the posterior region of the fiber mass (Fig. 9c). The ventral part of the fiber mass also shows a slight striation (Fig. 9d).
Harmothoe areolata (Polynoidae, Aciculata, Polychaeta)
The brain of the predatory scaleworm H. areolata is dominated by a pair of huge mushroom bodies (Fig. 6b). A detailed morphological description of these neuropils has already been provided elsewhere [see ]. Emerging from two large aggregations of small diameter globuli cells located dorsally in the prostomium, each mushroom body neuropil forms a well-defined lobe anteriorly and several median extensions posteriorly. The latter establish a close connection not only with the central neuropil but also with a clearly delineated cluster of glomeruli lying in the ventro-posterior part of the brain. A second group of glomeruli is situated within the anterior lobe of the mushroom bodies where it most likely receives input from the palpal nerve. The central neuropil itself consists of a largely undifferentiated meshwork of fibers. However, FMRF-amide-like immunoreactivity reveals a small, crescent-shaped neuropil concealed within the meshwork. This unpaired, poorly delineated neuropil is formed by several neurites that converge at the brain's midline.
Large and well-defined mushroom bodies showing a similar organization have also been observed in the polynoid representatives Lepidonotus clava (Fig. 2) and Sthenelais cf. limicola as well as in the aphroditid species Aphrodita aculeata and Neoleanira tetragona. Further neuroarchitectural similarities among scaleworm species include the presence of glomerular clusters (Fig. 2, Fig. 10a) and aggregations of fibers forming unpaired midline neuropils (Fig. 2, Fig. 11d, e).
Lumbricus terrestris (Lumbricidae, Oligochaeta, Clitellata)
The brain of the substrate feeding earthworm L. terrestris is dislocated posteriorly and lies on top of the esophagus in the third body segment. It is bilobed in shape, with each of the hemispheres sending out a prostomial nerve anteriorly (Fig. 6c). The brain is composed of a central neuropil and a dense cortex of neuronal somata that are not forming conspicuous clusters. The central fiber mass does not contain discernable neuropil subcompartments.
Hirudo medicinalis (Hirudinidae, Hirudinea, Clitellata)
The brain of the parasitic leech H. medicinalis is situated posteriorly to the medi an jaw in the fifth body segment (Fig. 6d). The brain is comparatively small and of a ribbon-like shape. Its central fiber mass is weakly differentiated into an anterior stratum comprising mostly columnar fiber elements and a posterior stratum comprising transverse fiber bundles. Neuronal cell somata are comparatively large and are arranged homogeneously around the cerebral neuropil. Dense aggregations of small-diameter neuronal somata are lacking and the central fiber mass is devoid of discernable substructures.
Leucophaea maderae (Blaberidae, Dictyoptera, Insecta)
The neuroanatomy of the cockroach L. maderae largely corresponds to the ground pattern found in pterygote insects [for an overview see e.g. [30, 31]]. Distinctive neuropils of the brain are the paired mushroom bodies (Fig. 1a) and the unpaired central body (Fig. 9a). Immunoreactivity towards a Horseradish-peroxidase antiserum reveals the principal organization of the mushroom body neuropils: Aggregations of tightly assembled globuli cell somata(i n insects termed Kenyon cells) give rise to a neuropil that shows a characteristic subdivision into a dorsal calyx region, embedded within the globuli cell bodies, a stalk-like peduncle, and an arrangement of terminal lobes.
The central body is an unpaired neuropil that spans the midline of the brain. It is part of the central complex, an assembly of interconnected neuropils situated roughly at the center of the brain. Within the central body, neurites are arranged in distinctive columnar and tangential fiber bundles.
The current study presents data obtained from immunohistochemically stained preparations of representatives of more than 20 annelid taxa. Antisera against the near-ubiquitous neuroactive substances serotonin, FMRF-amide, and histamine were used in combination with a nuclear marker to label limited subsets of neurons in the brain. Immunohistochemistry did not aim at identifying the transmitter composition of the brain but at revealing the presence and architecture of higher cerebral centers.
The most prominent neuropil structures to be encountered in the annelid brain are the paired mushroom bodies that occur in a number of polychaete representatives. Mushroom bodies could in some cases be demonstrated to be closely associated with clusters of spheroid neuropils reminiscent of arthropod olfactory glomeruli. Less distinctive subcompartments of the annelid brain are unpaired midline neuropils which have been encountered in several polychaete representatives and which bear a remote resemblance to similar components in the arthropod brain.
Mushroom bodies are lobed neuropils that are formed by the processes of thousands of small-diameter globuli cells located dorsally in the invertebrate central nervous system . In arthropods, mushroom bodies are usually easily recognizable not only due to their characteristic shape , but also due to the fact that glial sheaths clearly delineate the neuropil from the surrounding neuronal tissue . Incontrast to insects, the absence of cell nuclei dispersed along the borders of polychaete mushroom body neuropils (Figs. 1, 9, 10) indicates a lack of likewise well-developed glial boundaries in the brain. Thus, borders of cerebral subcompartments like the mushroom bodies are often only barely perceptible by differences in tissue density and structure (Figs. 9, 10). Among the investigated species, clearly demarcated mushroom bodies have been observed in Nereis diversicolor and the scale worm species Harmothoe areolata, Lepidonotus clava, Sthenelais cf. limicola, and Aphrodita aculeata. In these species, densely assembled globuli cells form well-defined aggregations in the dorsal part of the brain, which give rise to lobed neuropils that are clearly distinguishable within the cerebral fiber mass (Fig. 8c, d, Fig. 10a).
Elaborate mushroom bodies are also present in the brain of Hesione pantherina, but show a slightly different organization. They also originate from dorsal aggregations of globuli cells, but instead of forming an arrangement of terminal lobes, the stem-like neuropils of both hemispheres appear to be contiguous, forming a continuum across the midline of the brain (Fig. 8b). This condition bears resemblance to the contiguity of mushroom bodies that is observed in chelicerates and onychophorans .
Mushroom body neuropils are less conspicuous in other polychaete species. The dorsal part of the brain of Nephtys hombergii contains well-defined globuli cell clusters, but the associated neuropils are only weakly demarcated and barely discernable from the surrounding fiber mass (Fig. 10b). The borders of the globuli cell clusters in Phyllodoce maculata appear somewhat diffuse due to the loose assembly of the cell bodies. The boundaries of the stalk-like neuropils that emanate from the globuli cell clusters are also just faintly delineated and become obliterated as the neuropils of both sides converge towards the midline of the brain (Fig. 10c), so that a contiguous mushroom body organization in this species could not be ascertained.
In other polychaetes, lobed neuropil subcompartments are not discernable at all, although conspicuous clusters of small-diameter cells - usually indicative of mushroom bodies - are present. Odontosyllis cf. fulgurans, Tomopteris helgolandica, and the scolecid species Ophelia limacina all exhibit clusters of minute cell bodies but lack distinctive neuropils associated with them. Instead, the cell somata assemblies surround protuberances of the cerebral neuropil that extend into the core of the clusters. The protuberances can be small and undifferentiated, as observed in T. helgolandica (Fig. 10d) and O. limacina (Fig. 3b), or can show minor branching patterns, as evident in the anterior cluster of O. cf. fulgurans(Fig. 10e). The occurrence of two completely separated cell clusters, situated anteriorly and posteriorly in each hemisphere, is an exceptional characteristic of the brain of O. cf. fulgurans. T. helgolandica and O. limacina exhibit only a single cell clusters per hemisphere, situated at a posterior position in the brain. The posterior location of these presumptive globuli cell clusters, as well as the apparent lack of associated neuropil subcompartments within the main fiber mass of the brain must be addressed as a possible pitfall in the identification of mushroom bodies in these species. With respect to the lack of a distinct neuropil, the observed structures might be interpreted as primordial, poorly differentiated mushroom bodies, similar to the mushroom body-like structures that have been described in polyclad platyhelminthes [32, 36–38]. However, contrary to the condition in T. helgolandica and O. limacina, the globuli cells in platyhelminthes are reported to reside at the anterior-lateral border of the brain. Given the lack of a general, specific marker for globuli cells , tests for a possible immunoreactivity of the globuli-like cells against taurine, aspartate, and glutamate might provide a means to clarify the true identity of these neural structures in the polychaetes. In insects, antibodies directed against these neuroactive amino acids have been shown to produce immunostaining in specific subpopulations of globuli cells . However, preliminary studies employing taurine-antisera on vibratome sections of N. diversicolor generate d only diffuse and probably unspecific staining in the mushroom bodies (unpublished observation). Thus, evidence for the presence of mushroom bodies in O. cf. fulgurans. T. helgolandica and O. limacina remains inconclusive so far.
A specific marker for globuli cells would also be beneficial for a closer investigation of the dense cell body assemblies that have been observed in two more polychaete taxa, Eunice torquata and Lumbrineris cf. fragilis (Fig 5b, c, Fig. 10f). In these species, minute cells show a significantly different distribution than in other polychaete representatives. The cell aggregations are not restricted to comparatively small regions of the brain but form a single mass that surrounds the anterior part of the cerebral fiber mass in E. torquata, and in L. cf. fragilis extends to encase the fiber mass almost completely. Due to their predominant distribution and the absence of distinctive neuropils within the brain, the cell clusters cannot be regarded as indicative of the presence of mushroom body-like neuropils in these species at the present state.
Neuroanatomical analyses provided no evidence for the occurrence of mushroom body neuropils in Arenicola marina, the terebellid species Eupolymnia nebulosa, Pista cristata, and Telephus cincinnatus, the sabellid species Branchiomma bombyx and Sabella penicillus, as well as in the clitellate representatives Hirudo medicinalis and Lumbricus terrestris.
Detailed investigations in N. diversicolor, H. areolata, and L. clava have shown that mushroom bodies in these species share many neuroarchitectural similarities with their arthropod namesakes [25, 28]. Recently, such anatomy-derived homology assessments have been backed up by developmental studies investigating gene expression patterns in larvae of the nereid polychaete Platynereis dumerilii . The brain of adult P. dumerilii contains mushroom body neuropils that are strikingly similar to those of N. diversicolor. During ontogeny, the mushroom body anlagen of P. dumerilii are observed to express the same combination of genes that is characteristic for the developing mushroom bodies of Drosophila melanogaster, namely dachshund (Dach), pax6, brain factor 1 (BF1), and seven up (Svp) in the absence of eyes absent (Eya) and sine oculis (So). The investigation of additional genes reported to be expressed in the mushroom bodies of D. melanogaster reveals further similarities in the 'molecular fingerprint' of the mushroom bodies. In light of the 'new animal phylogeny' , these studies provide independent and therefore significant support for the homology of globuli cells that constitute mushroom bodies in annelids and arthropods. If true, and mushroom bodies in widely separated phyla are indeed homologous and not the product of a purely convergent evolution [see ], they probably constitute ancient features of the bilaterian brain.
Olfactory glomeruli are spheroidal neuropils that represent first order integration centres for odour information . Usually occurring in clusters, such neuropils have been described in arthropods, molluscs, and vertebrates . The occurrence of olfactory glomeruli has also been reported for the polychaete species Arctonoe vittata GRUBE, 1855 and Nereis vexillosa GRUBE, 1851, where they relay information to mushroom body neuropils . The observations of the current study are largely in accordance with these descriptions, as olfactory glomeruli could be identified in nereid Nereis diversicolor and the scale worm species Harmothoe areolata, Lepidonotus clava, and Aphrodita aculeata. Furthermore, small globular subcompartments possibly representing olfactory glomeruli were also discovered in the brain of Hesione pantherina (Fig. 9c). Considering that in arthropods, olfactory glomeruli provide the predominant sensory input to the mushroom bodies , it is hardly surprising that the occurrence of olfactory glomeruli in the polychaete brain coincides with the presence of well-developed mushroom bodies. However, just like the mushroom body neuropils, olfactory glomeruli were observed to show varying degrees of differentiation between different species. The most pronounced glomerular clusters were observed in H. areolata, while the glomeruli in L. clava and A. aculeata were less clearly demarcated. In N. diversicolor, the presence of olfactory glomeruli could only be confirmed by retrograde tracing experiments (unpublished observation). Thus, the occurrence of poorly differentiated olfactory glomeruli in the brain of polychaetes that possess equally poorly differentiated mushroom bodies (e.g. Nephtys hombergii) cannot be ruled out. Moreover, the possibility of a direct innervation of the mushroom bodies, as demonstrated for N. diversicolor , provides an alternative pathway for the transmission of odor information to the mushroom body neuropils that might also be utilized in other polychaete species.
The occurrence of two separate clusters of olfactory glomeruli in each brain hemisphere of H. areolata [compare ] is an exceptional neuroarchitectural condition not observed in any other of the investigated species. The discovery of olfactory glomeruli recieveing terminals of the palpal nerve and residing in close proximity to the mushroom body peduncle in N. diversicolor (unpublished observation) are reminiscent of the arrangement of the anterior glomerular cluster in H. areolata. This gives rise to speculations about the sensory input to the second, posteriorly located glomerular cluster in H. areolata. It seems conceivable that the posterior glomeruli are also involved in the processing of olfactory cues, possibly receiving chemosensory input from the nuchal organs situated at the posterior margin of the prostomium  and relaying information to the mushroom bodies. However, our immunostainings did not provide data to confirm such a pathway.
Unpaired midline neuropils
In this account, the general term 'unpaired midline neuropil' is applied to hitherto unspecified neuropils that span the midsagittal plane of the brain; the term does not imply homology between individual unpaired midline neuropils encountered in different species.
Unpaired midline neuropils have been observed in only a limited number of the investigated annelid species (Fig. 11). This might well be due to the fact that these cerebral substructures - in contrast to arthropod midline neuropils, such as the tetraconate central body or the chelicerate arcuate body - do not show definite boundaries in the form of glial sheaths. Instead, the midline neuropils were found to be tightly interwoven with the surrounding fiber mass and were only distinguishable if the neuropil showed pronounced immunoreactivity towards the applied antiserum. Unpaired midline neuropils occurred only in polychaete representatives and exhibited different degrees of differentiation. The simplest organization was encountered in Nereis diversicolor, where the unpaired midline neuropil consists of a small, crescent-shaped fiber tangle with no apparent internal differentiation (Fig. 11b). A more complex organization was observed in the unpaired midline neuropil of Eunice torquata, which comprises commissural elements that are linked by an arrangement of discrete fiber bundles (Fig. 11c). The unpaired midline neuropils in the polynoid species Harmothoe areolata and Lepidonotus clava are situated in the ventral part of the brain and can be considered homologous due to their architectural commonalities. The neuropils consist of fiber tangles that comprise ramifications of neurites that extend along the lateral axis of the brain, forming characteristic intersections (Fig. 11d, e). Their neuronal somata are located in two groups on both sides of the brain. In L. clava, additional fibers could be observed to enter the neuropil perpendicularly (Fig. 11e).
Among the unpaired midline neuropils of the polychaete brain, those observed in L. clava and E. torquata bear faint resemblance to midline neuropils of the arthropod brain. The perpendicular arrangement of neurite bundles, particularly in E. torquata, is reminiscent of the tangential and columnar organization of the central body in tetraconates (Fig. 11a) or the arcuate body in chelicerates. However, in the polychaetes, the fiber bundles do not appear to form distinct layers or the chiasmic patterns that are characteristic for unpaired components in the arthropod central nervous system . Furthermore, the specific connectivities of these neuropils to other parts of the polychaete brain still remain inconclusive, impeding attempts at homologizing these structures with unpaired midline neuropils in arthropods.
Evolution of annelid brain complexity
For lack of a well-resolved and robust annelid phylogeny, genera were grouped according to the cladistic analysis provided by Rouse and Fauchald . Although recent molecular studies have demonstrated that the major clades proposed by Rouse and Fauchald cannot be regarded as monophyletic groupings [4, 14], the provisional classification of the investigated species into Clitellata, Scolecida, Canalipalpata, and Aciculata serves to show that the occurrence of mushroom bodies is largely restricted to aciculate representatives. Outside Aciculata, conspicuous cell clusters possibly indicating the presence of mushroom body neuropils were only observed in the scolecid genus Ophelia. However, the similar cell clusters in the closely related Scalibregma species were not interpreted as mushroom bodies due to the lack of a core neuropil, discouraging the notion that the structures in Ophelia species indeed represent mushroom body neuropils.
Aciculata retains the highest support among the clades proposed by Rouse and Fauchald [4, 10, 14], containing most of the species that had formerly been united in the grouping 'Errantia'. The presence of mushroom bodies in errant polychaetes - characterized by a motile, often predatory or scavenging lifestyle and equipped with a variety of well-developed sensory organs - seems understandable in light of the presumptive function of these brain centers. Among arthropods, mushroom bodies are best investigated in insects, where they are generally assumed to act as integrative brain centers that play a cardinal role in olfactory processing and spatial, associative, and context-dependent learning and memory [42, 46]. Commonalities in the neuroarchitectural organization and integration of annelid and arthropod mushroom bodies point towards a similar function of these neuropils in the brain of aciculate polychaetes. It is easily imaginable how such cognitive abilities could translate into an evolutionary advantage in free-living animals that have to adapt their behavior to changing environmental demands. For example, learning, memory formation, and decision-making have been shown to correlate positively with fitness by increasing foraging success  and growth rate  in insects. In terms of mushroom body morphology, comparative neuroanatomical studies in beetles have revealed neuropil structure to be linked with the evolution of different feeding ecologies, as generalist feeders usually display larger and more complex mushroom bodies than specialist feeders . In other insects, mushroom body size has been demonstrated to correlate positively with learning abilities and to be influenced by experience . These studies from arthropods indicate that mushroom bodies could be of a similar adaptive value in coordinating prey finding, predator avoidance, mate choice, and other behaviors in errant polychaetes. However, cognitive abilities come at a price, since information processing and storing, as well as the development and maintenance of neural structures involved in learning and memory, are energetically costly [50–52]. The evolutionary tradeoff between information processing capacity and other fitness-related traits [51, 52] might provide an explanation for the relatively simple neuroanatomy and the lack of mushroom bodies observed in other polychaetes, as well as in clitellate representatives. In taxa living in comparatively consistent environments, the fitness gain associated with learning and memory abilities can be expected to become negligible in relation to the costs involved in building and maintaining a suitably complex nervous system. This notion finds further support in the apparent dispensability of elaborate sensory structures (e.g. eyes, palps, antennae, cirri, nuchal organs) in most sedentary and infaunal annelid species. Thus, the relatively simple neuroarchitecture observed in infaunal/sedentary annelids with a detritus/suspension feeding ecology can probably be attributed to selective pressures that do not favor the evolution of complex brains.
However, the varying grades of cerebral complexity observed in different annelids give rise to the question whether the simple neuroarchitecture and the lack of mushroom bodies in non-aciculate annelids is to be interpreted as an ancient evolutionary trait, or rather as a result of a secondary reduction in complexity? In keeping with the traditional view of animal evolution, as a gradual progress from simple to ever more complex forms, annelid mushroom bodies could intuitively be interpreted as a derived, unifying feature of aciculate polychaetes. However, one of the central implications of the 'new animal phylogeny' is that metazoan evolution can no longer be regarded as a gradual succession of increasingly complex forms and that secondary simplifications and reversals are probably far more wide-spread than formerly thought.
Regressive changes in neural complexity are commonly attributed to a narrowing of the ecological niche in a monotonous and extremely simplified environment and a cessation of mobile life , and can also be observed in sessile, semi-sessile, and parasitic forms of other taxa . The nervous system in none-parasitic cirripedes, for example, is much simpler than that of free-swimming Crustacea, lacking a distinctive tripartition and comprising only an estimated 200 neurons in Balanus nubilus. However, the presence of a more elaborate central nervous system in the barnacle cypris larva shows that the simple nervous system of the adult form results from a partly neural degeneration after settlement, and illustrates the need for coordinating a response to settlement cues in the vagile form [56, 57]. Similarly, the nervous system of the highly derived, parasitic rhizocephalic cirripeds is largely reduced. Comparable trends can also be observed in bivalve molluscs, in brachiopods, and in parasitic cestodes, illustrating that comparatively simple neuroarchitectures do not necessarily reflect ancestral conditions.
The problem of dealing with secondary character losses is also reflected in the cladistic analysis of Rouse and Fauchald , which placed Clitellata at a basal position in the annelid radiation - an inference that was brought about by the extensive lack of morphological structures in clitellates (e.g. palps, nuchal organs, parapodia, etc.) and the indiscriminative 'absent/present' coding in the character matrix [11, 13]. In contrast, recent molecular studies [4, 14] suggest that clitellates are derived polychaetes, which would render the Polychaeta paraphyletic. However, these studies have also not been able to provide a robust and convincing resolution for the root of the annelid radiation, proposing a basal position of chaetopterids, magelonids, and/or oweniids. A different approach in the quest to identify the most basal annelid taxa lies in outlining evolutionary scenarios to characterize the ground pattern of annelids on the basis of morpho-functional considerations [13, 58, 59]. Such studies propose that the annelid stem species was a marine organism  with a homonomously segmented body, biramous parapodia, pygidial cirri, and a large prostomium with palps and antennae . Among recent annelids, this organization largely corresponds to the bauplan of errant polychaetes.
It thus appears reasonable to attribute the simple neuroarchitecture and the prevalent lack of mushroom bodies in non-aciculate annelids to widespread secondary reductions in cerebral complexity, and to regard aciculate neuroanatomy as referring to the ancestral annelid condition. The presence of mushroom bodies is therefore probably an ancestral trait in annelids, which has been retained in aciculate polychaetes but has been lost in most other annelid taxa - a notion that is also in agreement with the argument presented in the previous paragraph. In this light, the tightly assembled cell somata observed in Ophelia might represent vestiges of largely reduced mushroom bodies. Though no neuroanatomical evidence for mushroom bodies could be detected in the investigated sedentary species, reports of mushroom bodies in Serpula  and in another sabellid (Strausfeld, personal communication) indicate that mushroom bodies have also been retained in some sedentary polychaete species.
Within aciculate polychaetes, evolutionary trajectories of mushroom body neuropils remain enigmatic. Varying grades of mushroom body differentiation in different species have led early authors to propose that polychaete mushroom bodies evolved from simple to increasingly complex structures, culminating in the elaborate neuropils of polynoid polychaetes [21, 22]. In the current study, polynoid polychaetes showed indeed the most complex neuroanatomy of all species investigated. However, in light of the arguments presented above, caution seems warranted in inferring phylogenetic implications from this observation. The largest and most elaborate mushroom bodies to be found in arthropods occur in the horseshoe crab Limulus polyphemus [60, 61] - commonly regarded as a living fossil.
C. M. H. and R. L. gratefully acknowledge the German Science Foundation (DFG) for funding this work as part of the priority program 'SPP 1174 - Deep Metazoan Phylogeny'. Thanks go to the staff of Espeland Marine Biological Station (Bergen, Norway) and the crew of the R.V. Hans Brattström (University of Bergen/IMR).
- Brusca RC, Brusca GJ: Invertebrates. 2003, Sunderland, MA: Sinauer Associates, Inc, 2Google Scholar
- McHugh D: Molecular phylogeny of the Annelida. Can J Zool. 2000, 78: 1873-1884. 10.1139/cjz-78-11-1873.View ArticleGoogle Scholar
- Rouse GW, Pleijel F, Edgecombe G, Worsaae K, Giribet G: First combined molecular and morphological phylogenetic analyses of Annelida. J Morphol. 2008, 269 (12): 1462-Google Scholar
- Zrzavý J, Říha P, Piálek L, Janouškovec J: Phylogeny of Annelida (Lophotrochozoa): total-evidence analysis of morphology and six genes. BMC Evol Biol. 2009, 9: 189-10.1186/1471-2148-9-189.PubMed CentralView ArticlePubMedGoogle Scholar
- Martin P: On the origin of the Hirudinea and the demise of the Oligochaeta. Proc R Soc Lond B. 2001, 268: 1089-1098. 10.1098/rspb.2001.1616.View ArticleGoogle Scholar
- Clark RB: Systematics and phylogeny: Annelida, Echiura, Sipuncula. Chemical zoology Annelida, Echiura, Sipuncula. Edited by: Florkin M, Scheer BT. 1969, New York: Academic Press, 4: 1-68.Google Scholar
- Fauchald K, Rouse GW: Polychaete systematics: past and present. Zool Scripta. 1997, 26 (2): 71-138. 10.1111/j.1463-6409.1997.tb00411.x.View ArticleGoogle Scholar
- de Quatrefages A: Histoire naturelle des Annelés marins et d'eau douce. 1866, Paris: Librarie Encyclopédique de RoretGoogle Scholar
- Day JH: A monograph on the Polychaeta of Southern Africa. Volume British Museum (Natural History) Publication 656. 1967, London: British Museum (Natural History), 1-878.Google Scholar
- Rouse GW, Fauchald K: Cladistics and polychaetes. Zool Scripta. 1997, 26 (2): 139-204. 10.1111/j.1463-6409.1997.tb00412.x.View ArticleGoogle Scholar
- Rouse GW, Fauchald K: Recent views on the status, delineation and classification of the Annelida. Amer Zool. 1998, 38: 953-964.View ArticleGoogle Scholar
- Almeida WO, Christoffersen ML, Amorim DS, Garraffoni ARS, Silva GS: Polychaeta, Annelida, and Articulata are not monophyletic: articulating the Metameria (Metazoa, Coelomata). Rev Bras Zool. 2003, 20 (1): 23-57. 10.1590/S0101-81752003000100006.View ArticleGoogle Scholar
- Bartolomaeus T, Purschke G, Hausen H: Polychaete phylogeny based on morphological data - a comparison of current attempts. Hydrobiologia. 2005, 535/536: 341-356. 10.1007/s10750-004-1847-5.View ArticleGoogle Scholar
- Struck TH, Schult N, Kusen T, Hickman E, Bleidorn C, McHugh D, Halanych KM: Annelid phylogeny and the status of Sipuncula and Echiura. BMC Evol Biol. 2007, 7: 57-10.1186/1471-2148-7-57.PubMed CentralView ArticlePubMedGoogle Scholar
- Hessling R: Novel aspects of the nervous system of Bonellia viridis (Echiura) revealed by the combination of immunohistochemistry, confocal laser-scanning microscopy and three-dimensional reconstruction. Hydrobiologia. 2003, 496: 225-239. 10.1023/A:1026153016913.View ArticleGoogle Scholar
- Wanninger A, Koop D, Bromham L, Noonan E, Degnan BM: Nervous and muscle system development in Phascolion strombus (Sipuncula). Dev Genes Evol. 2005, 215: 509-518. 10.1007/s00427-005-0012-0.View ArticlePubMedGoogle Scholar
- Kristof A, Wollesen T, Wanninger A: Segmental mode of neural patterning in Sipuncula. Current Biology. 2008, 18 (15): 1129-1132. 10.1016/j.cub.2008.06.066.View ArticlePubMedGoogle Scholar
- Orrhage L, Müller MCM: Morphology of the nervous system of Polychaeta (Annelida). Hydrobiologia. 2005, 535/536: 79-111. 10.1007/s10750-004-4375-4.View ArticleGoogle Scholar
- Zanol J, Fauchald K: Integrative approach using cLSM, SEM, and molecular data to understand the phylogeny of the family Eunicidae (Bristle Worms, Polychaetes, Annelida). J Morphol. 2008, 269 (12): 1465-Google Scholar
- Holmgren N: Zur vergleichenden Anatomie des Gehirns von Polychaeten, Onychophoren, Xiphosuren, Arachniden, Crustaceen, Myriapoden und Insekten. Kungl Svenska Vetenskaps Handl. 1916, 56: 1-315.Google Scholar
- Hanström B: Untersuchungen über die relative Größe der Gehirnzentren verschiedener Arthropoden unter Berücksichtigung der Lebensweise. Z Zellforsch Mikrosk Anat. 1927, 7: 135-190.Google Scholar
- Hanström B: Vergleichende Anatomie des Nervensystems der wirbellosen Tiere unter Berücksichtigung seiner Funktion. 1928, Berlin, Heidelberg, New York: Julias SpringerGoogle Scholar
- Aguinaldo AM, Turbeville JM, Linford LS, Rivera MC, Garey JR, Raff RA, Lake JA: Evidence for a clade of nematodes, arthropods and other moulting animals. Nature. 1997, 387: 489-493. 10.1038/387489a0.View ArticlePubMedGoogle Scholar
- Halanych KM, Bacheller JD, Aguinaldo AM, Liva SM, Hillis DM, Lake JA: Evidence from 18S ribosomal DNA that the lophophorates are protostome animals. Science. 1995, 267 (5204): 1641-1643. 10.1126/science.7886451.View ArticlePubMedGoogle Scholar
- Heuer CM, Loesel R: Immunofluorescence analysis of the internal brain anatomy of Nereis diversicolor (Polychaeta, Annelida). Cell Tissue Res. 2008, 331: 713-724. 10.1007/s00441-007-0535-y.View ArticlePubMedGoogle Scholar
- Loesel R, Heuer CM: The mushroom bodies - prominent brain centers of arthropods and annelids with enigmatic evolutionary origin. Acta Zool. 2010, 91: 29-34. 10.1111/j.1463-6395.2009.00422.x.View ArticleGoogle Scholar
- Tomer R: The evolution of mushroom body and telencephalic cell types, studied by single cell expression profiling of Platynereis dumerilii larvae. PhD thesis. 2009, University of Heidelberg, retrieved (02.10.2009), [http://www.ub.uni-heidelberg.de/archiv/9582]Google Scholar
- Heuer CM, Loesel R: Three-dimensional reconstruction of mushroom body neuropils in the polychaete species Nereis diversicolor and Harmothoe areolata (Phyllodocida, Annelida). Zoomorphology. 2009, 128 (3): 219-226. 10.1007/s00435-008-0063-7.View ArticleGoogle Scholar
- Rodriguez J, Deinhard F: Preparation of a semipermanent mounting medium for fluorescent antibody studies. Virology. 1960, 12: 316-7. 10.1016/0042-6822(60)90205-1.View ArticlePubMedGoogle Scholar
- Strausfeld NJ: Atlas of an insect brain. 1976, Heidelberg: SpringerView ArticleGoogle Scholar
- Homberg U: Distribution of neurotransmitters in the insect brain. 1994, Stuttgart: FischerGoogle Scholar
- Strausfeld NJ, Hansen L, Li Y, Gomez RS, Ito K: Evolution, discovery, and interpretation of arthropod mushroom bodies. Learn Mem. 1998, 5: 11-37.PubMed CentralPubMedGoogle Scholar
- Farris SM, Roberts NS: Coevolution of generalist feeding ecologies and gyrencephalic mushroom bodies in insects. Proc Natl Acad Sci USA. 2005, 102: 17394-17399. 10.1073/pnas.0508430102.PubMed CentralView ArticlePubMedGoogle Scholar
- Hähnlein I, Bicker G: Morphology of neuroglia in the antennal lobe and mushroom bodies of the brain of the honeybee. J Comp Neurol. 1996, 367: 235-245. 10.1002/(SICI)1096-9861(19960401)367:2<235::AID-CNE6>3.0.CO;2-6.View ArticlePubMedGoogle Scholar
- Strausfeld NJ, Strausfeld CM, Loesel R, Rowell D, Stowe S: Arthropod phylogeny: onychophoran brain organization suggests an archaic relationship with a chelicerate stem lineage. Proc R Soc Lond B. 2006, 273: 1857-1866. 10.1098/rspb.2006.3536.View ArticleGoogle Scholar
- Hadenfeldt D: Das Nervensystem von Stylochoplana maculata und Notoplana atomata. Z wiss Zool. 1929, 133: 586-638.Google Scholar
- Turner RS: Observations on the central nervous system of Leptoplana acticola. J Comp Neurol. 1946, 85: 53-65. 10.1002/cne.900850106.View ArticlePubMedGoogle Scholar
- Keenan CL, Coss R, Koopowitz H: Cytoarchitecture of primitive brains: Golgi studies in flatworms. J Comp Neurol. 1981, 195: 697-716. 10.1002/cne.901950412.View ArticlePubMedGoogle Scholar
- Johard HAD, Enell LE, Gustafsson E, Trifilieff P, Veenstra JA, Nässel DR: Intrinsic neurons of Drosophila mushroom bodies express short neuropeptide F: relations to extrinsic neurons expressing different neurotransmitters. J Comp Neurol. 2008, 507 (4): 1479-1496. 10.1002/cne.21636.View ArticlePubMedGoogle Scholar
- Sinakevitch I, Farris SM, Strausfeld NJ: Taurine-, aspartate- and glutamate-like immunoreactivity identifies chemically distinct subdivisions of Kenyon cells in the cockroach mushroom body. J Comp Neurol. 2001, 439: 352-367. 10.1002/cne.1355.View ArticlePubMedGoogle Scholar
- Adoutte A, Balavoine G, Lartillot N, Lespinet O, Prud'homme B, de Rosa R: The new animal phylogeny: reliability and implications. Proc Natl Acad Sci USA. 2000, 97 (9): 4453-4456. 10.1073/pnas.97.9.4453.PubMed CentralView ArticlePubMedGoogle Scholar
- Farris SM: Evolutionary convergence of higher brain centers spanning the Protostome-Deuterostome boundary. Brain Behav Evol. 2008, 72: 106-122. 10.1159/000151471.View ArticlePubMedGoogle Scholar
- Eisthen HL: Why are olfactory systems of different animals so similar?. Brain Behav Evol. 2002, 59: 273-293. 10.1159/000063564.View ArticlePubMedGoogle Scholar
- Strausfeld NJ, Hildebrand JG: Olfactory systems: common design, uncommon origins?. Curr Opin Neurobiol. 1999, 9 (5): 634-639. 10.1016/S0959-4388(99)00019-7.View ArticlePubMedGoogle Scholar
- Purschke G: Sense organs in polychaetes (Annelida). Hydrobiologia. 2005, 535/536: 53-78. 10.1007/s10750-004-4358-5.View ArticleGoogle Scholar
- Strausfeld NJ, Sinakevitch I, Brown SM, Farris SM: Ground plan of the insect mushroom body: functional and evolutionary implications. J Comp Neurol. 2009, 513: 265-291. 10.1002/cne.21948.View ArticlePubMedGoogle Scholar
- Raine NE, Chittka L: The correlation of learning speed and natural foraging success in bumble-bees. Proc R Soc Lond B. 2008, 275: 803-808. 10.1098/rspb.2007.1652.View ArticleGoogle Scholar
- Dukas R, Bernays EA: Learning improves growth rate in grasshoppers. Proc Natl Acad Sci USA. 2000, 97 (6): 2637-2640. 10.1073/pnas.050461497.PubMed CentralView ArticlePubMedGoogle Scholar
- Snell-Rod EC, Papaj DR, Gronenberg W: Brain size: a global or induced cost of learning?. Brain Behav Evol. 2009, 73: 111-128. 10.1159/000213647.View ArticleGoogle Scholar
- Laughlin SB, Stevenick de Ruyter van RR, Anderson JC: The metabolic cost of neural information. Nature Neurosci. 1998, 1 (1): 36-41. 10.1038/236.View ArticlePubMedGoogle Scholar
- Dukas R: Costs of memory: ideas and predictions. J Theor Biol. 1999, 197: 41-50. 10.1006/jtbi.1998.0856.View ArticlePubMedGoogle Scholar
- Mery F, Kawecki TJ: A fitness cost of learning ability in Drosophila melanogaster. Proc R Soc Lond B. 2003, 270: 2465-2469. 10.1098/rspb.2003.2548.View ArticleGoogle Scholar
- Kaufman ZS: Some problems of regressive evolution. Biol Bull. 2008, 35 (3): 318-326. 10.1134/S106235900803014X.View ArticleGoogle Scholar
- Bullock TH: Grades in neural complexity: how large is the span?. Integr Comp Biol. 2002, 42: 757-761. 10.1093/icb/42.4.757.View ArticleGoogle Scholar
- Gwilliam GF: Neurobiology of barnacles. Barnacle biology. Edited by: Southward AJ. 1987, Rotterdam: Balkema, 191-211.Google Scholar
- Harrison PJH, Sandeman DC: Morphology of the nervous system of the barnacle cypris larva (Balanus amphitrite Darwin) revealed by light and electron microscopy. Biol Bull. 1999, 197: 144-158. 10.2307/1542611.View ArticleGoogle Scholar
- Harzsch S: Neurophylogeny: Architecture of the nervous system and a fresh view on arthropod phylogeny. Integr Comp Biol. 2006, 46 (2): 162-194. 10.1093/icb/icj011.View ArticlePubMedGoogle Scholar
- Westheide W, McHugh D, Purschke G, Rouse G: Systematization of the Annelida: different approaches. Hydrobiologia. 1999, 402: 291-307. 10.1023/A:1003713230485.View ArticleGoogle Scholar
- Purschke G: On the ground pattern of Annelida. Org Div Evol. 2002, 2: 181-196. 10.1078/1439-6092-00042.View ArticleGoogle Scholar
- Fahrenbach WH: The brain of the horseshoe crab (Limulus polyphemus) II. Architecture of the corpora pedunculata. Tissue Cell. 1977, 9: 157-166. 10.1016/0040-8166(77)90056-8.View ArticlePubMedGoogle Scholar
- Fahrenbach WH: The brain of the horseshoe crab (Limulus polyphemus) III. Cellular and synaptic organization of the corpora pedunculata. Tissue Cell. 1979, 11: 163-200. 10.1016/0040-8166(79)90016-8.View ArticlePubMedGoogle Scholar
- Fauchald K, Jumars PA: The diet of worms: A study of polychaete feeding guilds. Oceanogr Mar Biol. 1979, 17: 193-284.Google Scholar
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